A Chemoptogenetic Tool for Spatiotemporal Induction of Oxidative DNA Lesions In Vivo

Oxidative nuclear DNA damage increases in all tissues with age in multiple animal models, as well as in humans. However, the increase in DNA oxidation varies from tissue to tissue, suggesting that certain cells/tissues may be more vulnerable to DNA damage than others. The lack of a tool that can control dosage and spatiotemporal induction of oxidative DNA damage, which accumulates with age, has severely limited our ability to understand how DNA damage drives aging and age-related diseases. To overcome this, here we developed a chemoptogenetic tool that produces 8-oxoguanine (8-oxoG) at DNA in a whole organism, Caenorhabditis elegans. This tool uses di-iodinated malachite green (MG-2I) photosensitizer dye that generates singlet oxygen, 1O2, upon fluorogen activating peptide (FAP) binding and excitation with far-red light. Using our chemoptogenetic tool, we are able to control generation of singlet oxygen ubiquitously or in a tissue-specific manner, including in neurons and muscle cells. To induce oxidative DNA damage, we targeted our chemoptogenetic tool to histone, his-72, that is expressed in all cell types. Our results show that a single exposure to dye and light is able to induce DNA damage, promote embryonic lethality, lead to developmental delay, and significantly reduce lifespan. Our chemoptogenetic tool will now allow us to assess the cell autonomous versus non-cell autonomous role of DNA damage in aging, at an organismal level.


Introduction
Reactive oxygen species (ROS) are produced continually through life and have physiological and pathological ramifications. ROS can cause oxidative damage to macromolecules including DNA, RNA, lipids, and proteins, but is also known to play a critical role in signaling cascades [1,2]. The oxidative stress theory of aging has been controversial, with studies that have shown both beneficial and detrimental effects of ROS [2][3][4]. Stemming from multiple studies, current view posits that the level of ROS, as well as the spatial and temporal context, is critical when understanding the role of ROS.
Exposure to exogenous and endogenously produced ROS drives oxidative DNA damage and is a challenge to genome stability [5,6]. Oxidative DNA damage is highly variable between cell types and tissues, not only in absolute lesion numbers but also distribution over the genome [7][8][9][10][11][12][13]. Oxidative DNA damage is associated with aging and multiple age-related diseases, including neurodegeneration and cancer. Chemotherapeutic agents used to treat cancer patients cause oxidative DNA damage and contribute to longterm side effects including premature aging syndromes such as frailty [14,15]. It is welldocumented that oxidative nuclear DNA damage increases in all tissues with age [16,17].
To screen, about 50 individual F1 rollers were isolated onto separate OP50 plates and allowed to have progeny prior to genotyping by PCR. Single F1 rollers were lysed by WLB (10 mM Tris-Cl, pH 8.2, 50 mM KCl, 2.5 mM MgCl 2 , 0.45% Tween 20, 0.05% gelatin) with 1 mg/mL proteinase K at 60 • C for 1 h, and proteinase K was inactivated at 95 • C for 15 min. The insertion site was PCR amplified to see differences in size, and non-roller F2s from positive F1 plates were picked individually and genotyped for homozygotes. Final positive homozygotes were kept several generations and observed no visible morphological or behavior defects. The insertion site including upstream and downstream of fap::gfp gene was PCR amplified and confirmed by sequencing.

MG-Dye Treatments and Red light Illumination
A whole plate of worms was washed along with OP50 into a glass petri dish in 3 mL M9 buffer. MG-ester (cell permeable dye that does not generate singlet oxygen) or MG-2I were added to a final concentration of 2 µM. The glass plates were shielded from light and placed on a shaker at 100 rpm at room temperature for the desired time. Experimental or control worms were pelleted by brief centrifugation and transferred onto OP50 plates. Red light illumination was performed with a customized LED (660 nm) box that delivers 89 mW/cm 2 intensity for desired time.

Behavior Analysis and Quantitation
Complete paralysis in eft-3p::fap::gfp worms was defined as unable to move even after gentle touch with a worm pick. Unc and coiled phenotype of unc-17p::ph::fap::gfp worms were defined as unable to move properly after touching and coiled body bends. To quantitate the percentage of paralysis, at least three independent experiments (with 30-60 animals each) were performed.
Pumping rate of myo-2p::fap::gfp worms were counted under standard dissecting microscope. To confirm intake of E. coli-GFP (a gift from Dr. Arjumand Ghazi), worms were transferred onto NGM plates with E. coli-GFP for 30 min and immobilized with sodium azide solution for imaging.

Immunostaining of Rad-51 Foci
After 16 hr soaking with MG-2I, FAP::GFP::HIS-72 expressing worms were treated with or without 20 min red light. The worms were placed on OP50 for 2.5 h before dissecting gonads for immunostaining. Immunostaining and analysis of RAD-51 foci [21] was performed following previously established protocol [22]. Briefly, day 1 (D1) adult gonads were dissected in 1X sperm salts (50 mM PIPES pH 7.0, 25 mM KCl, 1 mM MgSO 4 , 45 mM NaCl, and 2 mM CaCl 2 ) and fixed in 1% paraformaldehyde diluted in 1X sperm salts for 5 min in a humid chamber. Slides were then frozen on a metal block on dry ice for at least 10 min prior to flicking off the cover slip and immersing in methanol precooled in dry ice for 2 min. This was followed by 5 s in acetone at 4 • C. Slides were washed in PBST with BSA [1XPBS with 0.1% Tween and 0.1% bovine serum albumin (BSA)], and incubated overnight at 4 • C with primary antibody. Antibodies used: rabbit anti-RAD-51 (gift from Dr. Sarit Smolikove) and mouse Mab414 (gift from Dr. Judith Yanowitz). The next day, slides were washed 3× in PBST with BSA for 10 min and incubated with secondary antibody (goat anti-rabbit Alexa 594 and anti-mouse alexa 488, 1:1000 in PBST with BSA) for 2 h at room temperature in the dark. Slides were then washed 2 × 10 min in PBST with BSA. Slides were mounted in Prolong Gold with DAPI and put in the dark to cure overnight before imaging.

Embryonic Lethality and Developmental Delay
Twenty day 1 adults untreated (UT), with dye (+D) and dye+ light (+DL) were placed on OP50 seeded NGM plates in triplicate. After a one-hour egg lay, 40-60 eggs were transferred to a new plate in triplicates. The worms were grown at 20 • C for 36 h. Three independent experiments were performed.
Number of unhatched eggs versus total number of eggs was recorded (blinded to experimental group) as % embryonic lethality.
Number of non-adults (YA or larval stage) versus total number of hatched worms was recorded (blinded to experimental group) as development delay.

Lifespan Analysis
Lifespan analysis was performed as described [23], with a few changes. Briefly, 40-60 animals were used per conditions and scored every other day in a blinded manner. Day 1 adults were transferred to 2.5 µg/mL FUDR containing NGM plates and were maintained on FUDR for the rest of the lifespan analysis. All lifespan experiments were performed at 20 • C in a blinded fashion.

Imaging
For fluorescence imaging of FAP::GFP and MG-ester, worms were anesthetized with 10 mM sodium azide on 2% agarose pads. Images were captured on Leica SP8 confocal microscope with 20× or 63× objective. Images were processed by Leica software. Movies were captured on Zeiss SteREO equipped with AxioCam camera.

Statistics
All statistical analyses were performed with GraphPad Prism 8.0 (GraphPad Software, Inc., San Diego, CA, USA). Survival analyses were performed using the Kaplan-Meier method and the significance of differences between survival curves was calculated using the log rank (Mantel-Cox) test. Differences between groups were considered to be significant at a p value of <0.05. One way ANOVA was performed with multiple comparisons for most assays. Detailed information is in Figure Legends.

Systemic Induction of ROS Promotes Paralysis
We used a genetically encoded ROS generator, a fluorogen activating peptide (FAP) with high affinity for photosensitizer dye, malachite (MG-2I). FAP is a 25 kDa binding peptide for malachite green (MG) derivatives with a low-picomolar dissociation constant [24][25][26]. Excitation with far-red light allows for non-toxic penetration to tissues in live animals. FAP binding and excitation allows MG-2I to generate singlet oxygen, ( 1 O 2 ), locally ( Figure 1A). Note that 1 O 2 is highly reactive, with limited diffusion, and cannot be converted into other ROS, thus offering multiple advantages [27]. The FAP chemoptogenetic tool has been used for protein inactivation, targeted cell killing, and rapid targeted lineage ablation in vivo in zebrafish. However, the zebrafish model required microinjection [28,29] of the MG-2I dye, restricting its usage for any lifespan or healthspan assays. Therefore, we first wanted to test the penetration of the MG dye in vivo in C. elegans, since the worm is protected by a cuticle that acts as a barrier to chemical uptake. tool has been used for protein inactivation, targeted cell killing, and rapid targeted lineage ablation in vivo in zebrafish. However, the zebrafish model required microinjection [28,29] of the MG-2I dye, restricting its usage for any lifespan or healthspan assays. Therefore, we first wanted to test the penetration of the MG dye in vivo in C. elegans, since the worm is protected by a cuticle that acts as a barrier to chemical uptake. To overcome this challenge, we tested mutants with altered cuticle properties to increase permeability of the MG dye. The mutant, bus-5, encodes the dTDP-glucose 4,6dehydratase, rml-2, and is required for dTDP rhamnose biosynthesis and is suggested to be a cuticular component [30]. bus-5 (br19) has a compromised cuticle but retains integrity and biological function [31]. First, to test the systemic induction of ROS with our chemoptogenetic tool, we cloned the promoter of a ubiquitously expressed gene eft-3, a translation elongation factor 1-alpha homolog, to drive expression of FAP in worms. Here, FAP was tagged with GFP in frame (codon optimized with C. elegans introns) to track its expression and regulation by unc-54 3 UTR. We expressed this transcriptional reporter eft-3p::fap::gfp in bus-5 worms as an extrachromosomal array. The transgenic animals expressed GFP signal in all tissues throughout their lifespan, as expected ( Figure 1B,C). The transgenic worms that express eft-3p::fap::gfp showed diffuse green fluorescence in all cell types, except in the germline. Multiple independent lines were maintained for >3 generations before conducting further experiments. All transgenic animals were indistinguishable from bus-5 parental strains and did not exhibit any obvious morphological or behavior defects.
First, we injected the transgenic lines with MG-ester fluorogen to examine penetration of the dye in vivo. As seen in zebrafish, microinjection of MG-ester dye, which binds FAP but does not produce ROS, showed co-localization of red fluorescence (MG-ester) with green fluorescence (FAP-GFP) ( Figure 1C). However, injection with MG would limit longitudinal analysis of C. elegans for healthspan and lifespan measures. Therefore, we next tested soaking of transgenic worms with MG-ester for multiple time points in different life stages. Interestingly, soaking for 1, 4, and 24 hr showed co-localization of MG-ester signal with GFP, confirming that soaking for a short period allows cell permeability of the MG-ester dye. Additionally, the red fluorescence signal can be detected at all stages of worms, from larval to adults, suggesting intake of MG dye at a variety of life stages ( Figure 1C). For the next set of experiments, we used overnight soaking (~14-16 hr) with MG-2I, a di-iodinated derivative that has been previously shown to produce singlet oxygen upon excitation with far-red light ( Figure 1A). After illumination using an LED source at 660 nm, the transgenic worms were paralyzed immediately in a light exposure-dependent manner, retained a rigid posture for about 24 hr, and were eventually dead ( Figure 1D,E, Movies S1 and S2). Neither MG-2I dye treatment or red light illumination alone caused visible toxicity to bus-5 transgenic lines.

Chemoptogenetic Tool Allows for Temporal Induction of ROS
As we optimized MG delivery and induction with light in the bus-5 transgenic lines, we next wanted to optimize the system in wildtype (N2) C. elegans. We expressed the transcriptional reporter, eft-3p::fap::gfp in N2 worms as an extrachromosomal array. Soaking worms overnight (~14-16 hr) in MG-ester allowed for uptake in almost all tissues examined. Similar to bus-5, after 2 min illumination with far-red light, 50% of the transgenic animals were paralyzed, and within 5 min 100% of the population was paralyzed (Figure 2A). The N2 extrachromosomal array transgenic lines performed as well as the bus-5 line.
Since our goal is to use our FAP chemoptogenetic tool to induce oxidative damage through life and examine its role in aging, we wanted to test the temporal induction of ROS using our tool. Previously, it has been reported that FAP has a low-picomolar dissociation constant. Therefore, we wanted to test whether MG could be fed to young animals and be retained in the worm for extended period of time. The eft-3p::fap::gfp was integrated into N2 wildtype in order to ensure stable expression throughout lifespan. Strikingly, a single overnight soak at larvae (L4) stage allowed for MG-ester binding and fluorescence at least until day (D9) of adulthood ( Figure 2B). Since we expected eft-3p::fap::gfp integrated lines to retain low copy FAP, we used 20 min light exposure to examine paralysis. We tested whether light and MG-2I dye at different ages would be effective to induce paralysis as observed in young worms. After soaking with MG-2I overnight and exposure to 20 min red light, D5 and D9 adults paralyzed at the same rate compared to young D1 adults ( Figure 2C). Taken together, our data shows that the FAP-chemoptogenetic tool can be used to temporally induce ROS and is suitable to address lifespan and healthspan. Since our goal is to use our FAP chemoptogenetic tool to induce oxidative damage through life and examine its role in aging, we wanted to test the temporal induction of ROS using our tool. Previously, it has been reported that FAP has a low-picomolar dissociation constant. Therefore, we wanted to test whether MG could be fed to young animals and be retained in the worm for extended period of time. The eft-3p::fap::gfp was integrated into N2 wildtype in order to ensure stable expression throughout lifespan. Strikingly, a single overnight soak at larvae (L4) stage allowed for MG-ester binding and fluorescence at least until day (D9) of adulthood ( Figure 2B). Since we expected eft-3p::fap::gfp Figure 2. Chemoptogenetic tool can be used to induce oxidative damage in a temporal manner (A) N2 with eft-3p::fap::gfp as an extrachromosomal array was soaked in MG-2I overnight and illuminated with red light. Representative images of N2 integrated lines immediately after red light illumination. A total of 3 independent experiments were performed for each age group. Percent of paralyzed worms is plotted as mean ± SD.~30 worms were counted for each experiment. (B) N2 with eft-3p::fap::gfp integrated lines were soaked with MG-ester as L4 for 24 hr. Colocalization of GFP and MG-ester dye was followed-up in day (D1), D2, D3, D5, and D9 adults. Scale bar = 25 µm. (C) Quantitation of paralysis immediately after red light illumination for 20 min in N2 with integrated eft-3p::fap::gfp. A total of 3 independent experiments were performed for each age group. Paralysis rate is plotted by mean ± SD. A total of 30-60 worms were counted for each experiment.

Chemoptogenetic Tool Allows for Spatial Induction of ROS
Tissue-specific oxidative damage has been challenging to address since we need a tool that can be precise, sensitive, and adaptable to multiple tissues. To explore if the FAP-chemoptogenetic tool can specifically target certain tissues, we chose two tissues: neurons and pharyngeal pump ( Figure 3A). Genetically encoded and inducible tools for neuronal ablation have been in high demand to study neurodegeneration. However, there is no optogenetic tool that can be activated by near infrared light (NIF) light, which would allow deeper tissue penetration and cause drastically less damage in free living C. elegans.
To test the efficacy of neuron ablation with the FAP-chemoptogenetic system, we generated transgenic bus-5 worms that express FAP::GFP in cholinergic motor neurons, using the unc-17 promoter. Previous studies have reported target cell ablation can be achieved through localized ROS production [32,33]. Specifically, plasma membrane targeted ROS leads to lipid peroxidation at the membrane, driving neuronal cell ablation and promoting paralysis [33]. Therefore, the N terminal of FAP::GFP was tagged with a membrane targeting sequence, the PH (Pleckstrin Homology) domain from rat PLC-δ [34]. PH domain binds to phosphoinositides and targets FAP to the plasma membrane. By targeting FAP to the plasma membrane, we first wanted to test targeting singlet oxygen to lipids and promote neuronal cell ablation. Extrachromosomal unc-17p:ph::fap::gfp expressing bus-5 worms showed GFP expression in ventral and dorsal nerve cords and motor commissures ( Figure 3B), confirming FAP expression in cholinergic motor neurons. Worms expressing an extrachromosomal version of the transgene did not show any physiological or morphological defects. Soaking with MG-2I or MG-ester did not affect locomotion behavior. To examine neuronal ablation, we synchronized unc-17p:ph::fap::gfp transgenic worms at L4 stage and soaked them overnight with MG-2I. After exposure to MG-2I, and immediately after red light illumination, unc-17p:ph::fap::gfp transgenic worms were uncoordinated (Unc) and coiled, a phenotype that is correlated with cholinergic motor neuron ablation ( Figure 3C). Within 5 min of illumination, transgenic worms began to show various degrees of Unc phenotype. After 20 min of exposure to red light, 100% of the worms displayed Unc phenotype ( Figure 3D, Movies S3 and S4). Locomotion defects persisted 24 hr after exposure to light, suggesting permanent motor neuron death/ablation. The neuronal damage was confirmed under confocal microscopy ( Figure 3B). After 24 hr of red light illumination, dorsal neuron body and commissure was undetected, while the remaining ventral neurons displayed GFP puncta ( Figure 3B).
To test whether we can drive oxidative stress in the muscle, we targeted the pharynx, using the promoter of myosin heavy chain structural gene, myo-2. MYO-2 is abundantly expressed in the pharynx muscle and neuronal cells throughout lifespan ( Figure 3A). The transcriptional reporter Pmyo-2::FAP::GFP in bus-5 worms showed strong GFP signal in the pharynx, and normal morphology and behavior under basal conditions (Movie S5). Synchronized L4 worms were soaked with MG-2I and exposed to red light. Within 5 min of illumination,~100% worms ceased pumping ( Figure 3E), although they maintained normal body movement (Movie S6). Pharyngeal function is also required for efficient food intake. The pharyngeal pump consists of coordinated contraction and relaxation required for feeding. Fluorescently labeled bacterial intake can therefore inform of pharyngeal activity. Interestingly, blue light has shown to increase pumping rate and may therefore act as a limitation of other optogenetic tools. We exposed transgenic Pmyo-2::FAP::GFP worms to fluorescently labeled E. coli (OP50), and then exposed them to 660 nm red light for 5 min or left them unexposed to light. GFP OP50 was found in the gut of transgenic worms with no exposure to red light, but not after exposure to light and dye ( Figure 3F), suggesting that oxidative stress in the pharyngeal muscle inactivates pumping. Taken together, our data shows that the FAP-chemoptogenetic tool allows for spatial induction of oxidative damage in live animals.
Tissue-specific oxidative damage has been challenging to address since we need a tool that can be precise, sensitive, and adaptable to multiple tissues. To explore if the FAPchemoptogenetic tool can specifically target certain tissues, we chose two tissues: neurons and pharyngeal pump ( Figure 3A). Genetically encoded and inducible tools for neuronal ablation have been in high demand to study neurodegeneration. However, there is no optogenetic tool that can be activated by near infrared light (NIF) light, which would allow deeper tissue penetration and cause drastically less damage in free living C. elegans.  :gfp in bus-5, fed OP50 was quantified before and after 24 hr MG-2I dye soak and immediately following 5 min illumination with far-red light. Pumping rate was measured in the terminal bulb. A total of 3 independent experiments were performed. Pumping rate was plotted as mean ± SD. Pumping rate was determined from the mean of 10-12 worms for each experiment. Unpaired t-test was performed. *** p < 0.001. (F) myo-2p::fap::gfp were fed OP50-GFP for 30 min, followed by 24 hr MG-2I dye soak and 5 min illumination. Brightly fluorescing Escherichia coli (E. coli) OP50-GFP bacteria observed in digestive tract towards the tail in non-illuminated worms, but absent after exposure to light. Scale bar = 90 µm.

Chemoptogenetic Tool Allows for Oxidative DNA Damage
Our goal is to induce oxidative DNA damage in C. elegans and examine its role in healthspan and lifespan. Therefore, to test whether our chemoptogenetic tool can induce oxidative DNA damage, we tagged endogenous histone component, HIS-72, with FAP::GFP by CRISPR/Cas9. HIS-72 encodes H3.3-like protein and contains the evolutionarily conserved AAIG motif. HIS-72 is expressed ubiquitously in all tissues over the lifespan of worms, making it suitable for our study. Importantly, his-72::gfp or loss of his-72 did not affect lifespan in worms [35]. GFP::HIS-72 was tagged with FAP ( Figure 4A) and confirmed to ubiquitously express. We and others have previously shown that an increase in DNA damage results in embryonic lethality, measured as egg-hatching capacity. To test whether induction of oxidative DNA damage also results in unhatched embryos, we used FAP::GFP::HIS-72 expressing worms. Young adults were left untreated (UT); treated with dye overnight, MG-2I (+D) alone; or treated with dye and 660 nm light (+DL) for 20 min. Immediately after illumination, the adults were allowed to lay eggs for 1 h (F0 1 ) or after 24 hr post-exposure (F0 24 ).
Exposure to both dye and light significantly compromised egg hatching capacity in the F0 1 generation ( Figure 4B). Compared with control groups (untreated or with dye alone), the average hatching rate decreased by~50% in all three lines tested. Interestingly, embryonic lethality of the F0 24 was not affected, suggesting efficient DNA damage resolution and repair. DNA damage is also known to delay larval development, and is a measure to evaluate DNA damage, response, and repair efficiency. Consistent with other studies, oxidative DNA damage delayed the development of larvae from the stage-synchronized F0 1 population ( Figure 4C). We also examined RAD-51 foci in +D and +DL treated animals. RAD-51 is a DNA binding protein and mediator of DNA damage. Upregulated RAD-51 foci are indicative of increased DNA damage or repair defects. Immediately after exposure to dye and light, there was a significant increase in RAD-51 foci in the germline that was resolved with time ( Figure 4D,E), thus confirming that our chemoptogenetic tool can induce DNA damage in a targeted manner. Finally, we followed the lifespan of transgenic worms exposed to dye alone or dye + light. Interestingly, induction of oxidative DNA damage led to reduced lifespan, as evidenced in other DNA repair mutants ( Figure 4F). Therefore, taken together, these results validate that our chemoptogenetic tool can be used in vivo to drive oxidative DNA damage in C. elegans. and confirmed to ubiquitously express. We and others have previously shown that an increase in DNA damage results in embryonic lethality, measured as egg-hatching capacity. To test whether induction of oxidative DNA damage also results in unhatched embryos, we used FAP::GFP::HIS-72 expressing worms. Young adults were left untreated (UT); treated with dye overnight, MG-2I (+D) alone; or treated with dye and 660 nm light (+DL) for 20 min. Immediately after illumination, the adults were allowed to lay eggs for 1 h (F01) or after 24 hr post-exposure (F024).

Discussion
DNA is the primary template encoding genetic information, but it is constantly bombarded with damaging agents, making it surprisingly unstable [17,36]. DNA repair has been documented to decline with age, whereas nuclear DNA damage correlates with age-related pathologies, including, diabetes, cancer, and neurodegeneration. Thus, there is robust evidence for DNA damage as a major causal contributor to human aging and disease. Elegant studies have generated DNA endonuclease tools that can cause double strand DNA breaks (dsDNA) [37,38]. However, controlling the threshold of damage in such systems has been a challenge. Moreover, dsDNA breaks are rare and toxic (cause apoptosis), whereas oxidative DNA damage are very prevalent. Our results not only validate that our chemoptogenetic tool can cause DNA damage in C. elegans, but also confirms that oxidative DNA damage can drive aging.
FlAsH and ReAsH, KillerRed, and MiniSOG are genetically targeted photosensitizers that have been previously developed to produce ROS at specific targets in cells [33,[39][40][41][42][43]. These tools have been mainly used for cell ablation. However, some of the challenges with these photosensitizers has been that they require a very high light dose to produce ROS, and the spectral properties of these overlap with biological chromophores. This leads to the challenge of ROS production even in the absence of photosensitizers [44,45]. Similarly, blue light that is used to generate ROS by some of these photosensitizers is perceived as toxic in multiple animals, thus limiting the ability to examine healthspan and lifespan trajectories [45][46][47][48].
We generated a chemoptogenetic tool to directly test whether DNA damage alters aging hallmarks in a cell autonomous or non-cell autonomous manner. This technology offers significant advantages: (1) It acts in a very restricted radius and can be targeted to specific cells/tissues. (2) The fluorogen is only excited when bound to the FAP, which improves the signal to noise ratio. (3) The FAP and dye are not harmful until bound and excited. Hence, by targeting FAP to DNA, we will eliminate confounding effects of damage elsewhere. (4) This photosensitizer tool requires far-red light, thus can be used for deep-tissue applications. By controlling illumination time, one can closely control ROS dosage and local production.
This new chemoptogenetic ROS generator can be targeted to proteins in various cellular locations (mitochondria, lysosome, etc.) and can also be targeted to other biomolecules and tissues to delineate the interplay of the hallmarks of aging. Using this novel chemoptogenetic tool, we anticipate to uncover novel causal mechanisms and their direct link to aging and lifespan. The FAP-chemoptogenetic tool, therefore, holds significant promise to address major questions in the field of DNA damage and aging.

Institutional Review Board Statement: Not applicable.
Informed Consent Statement: Not applicable.

Data Availability Statement:
The data presented in this study are available in all figures (Figures 1-4).